Author Manuscript Published OnlineFirst on September 18, 2017; DOI: 10.1158/0008-5472.CAN-17-1701 Author manuscripts have been peer reviewed and accepted for publication but have not yet been edited.
RXRA and PPARG in Bladder Cancer
Genomic activation of PPARG reveals a candidate therapeutic axis in bladder cancer
Jonathan T. Goldstein1, Ashton C. Berger1, Juliann Shih1, Fujiko F. Duke1, Laura Furst1, David J. Kwiatkowski2, Andrew D. Cherniack1,3, Matthew Meyerson1,3,4,5 and Craig A. Strathdee1 Affiliations: 1The Broad Institute of MIT and Harvard, Cambridge, Massachusetts, United States of America. 2Brigham and Women's Hospital, Harvard Medical School, Boston, Massachusetts, United States of America, 3Department of Medical Oncology, Dana- Farber Cancer Institute, Boston, Massachusetts, United States of America, 4Center for Cancer Genome Discovery, Dana-Farber Cancer Institute, Boston, Massachusetts, United States of America. 5Department of Pathology, Harvard Medical School, Boston, Massachusetts, United States of America. Current address for F. Duke: Gritstone Oncology, Cambridge, MA USA.
Running title: RXRA and PPARG in bladder cancer Keywords: RXRA, PPARG, Genitourinary cancers: bladder, Nuclear receptors: structure and function
Additional information. Financial support: Financial support for this work was provided by Bayer AG (Berlin, Germany) (J.Goldstein, A.Berger, J.Shih, F.Duke, L.Furst, A.Cherniack, M.Meyerson, and C.Strathdee) and the National Cancer Institute under grant 5R35CA197568-02 (M. Meyerson). Corresponding Author: Matthew Meyerson, Dana-Farber Cancer Institute, Boston, MA, 02115, USA; Tel: 617-632-4768, Email: [email protected] Conflict of interest disclosure statement; The Broad Institute and Dana-Farber Cancer Institute have filed a patent application for aspects of the work described in this paper. Financial support for this work was provided by Bayer AG (Berlin, Germany). M. Meyerson is a member of the Scientific Advisory Board and equity holder of Origimed. 1
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RXRA and PPARG in Bladder Cancer
Abstract The PPARG gene encoding the nuclear receptor PPAR-gamma is activated
in bladder cancer, either directly by gene amplification or mutation, or indirectly
by mutation of the RXRA gene which encodes the heterodimeric partner of
PPAR-gamma. Here we show that activating alterations of PPARG or RXRA
lead to a specific gene expression signature in bladder cancers. Reducing
PPARG activity, whether by pharmacologic inhibition or genetic ablation,
inhibited proliferation of PPARG-activated bladder cancer cells. Our results
offer a preclinical proof of concept for PPARG as a candidate therapeutic target
in bladder cancer.
2
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RXRA and PPARG in Bladder Cancer
Introduction
Bladder cancer is the fifth most commonly diagnosed cancer in the United
States with an annual incidence of 80,000 cases and an annual mortality of
15,000. Most patients are diagnosed with non-invasive/superficial urothelial
carcinoma of the bladder and respond well to transurethral resection, Bacillus
Calmette-Guérin (BCG) immunotherapy, and regular cystoscopic surveillance,
with a 5-year survival rate of 96%. Patients diagnosed with muscle-invasive
disease have a poorer prognosis, however, with a 5-year survival rate of 35-
70%, depending upon the extent of invasion, regional and systemic
metastases, and response to therapy.
Recently several immune checkpoint blockade drugs have been FDA-
approved for treatment of urothelial carcinoma, including atezolizumab, an anti-
PD-L1 antibody, in 2016 (1); nivolumab and pembrolizumab, anti-PD-1
antibodies, in 2017 (2) ; and avelumab and durvalumab, anti-PD-L1 antibodies,
in 2017 (3,4). These approvals mark the first new drugs for metastatic bladder
cancer in over 20 years. However, the objective response rates (defined using
RECIST v1.1) were relatively low in these clinical trials, with 15-20% overall
response rate and 26-28% response rate in PD-L1-positive patients (1,2).
Beyond checkpoint inhibitors, a number of therapies targeting specific genetic
alterations, including FGFR3 alterations, mTOR pathway alterations, and DNA
repair deficiencies associated with ERCC2 alterations (5-8), are under clinical
3
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RXRA and PPARG in Bladder Cancer
evaluation.
We explored large-scale cancer genome datasets derived from patients with
muscle-invasive bladder cancer with the purpose of identifying novel
therapeutic targets. Hotspot mutations (p.S427F/Y) in the retinoid X receptor
alpha (RXRA) gene are present in ~5% of bladder cancer samples (9,10).
RXRA is a well characterized ligand-activated nuclear receptor that serves as a
requisite heterodimer partner for ~30 nuclear receptors, including PPARA,
PPARG, PPARD, RARA, RARB, VDR, TR, LXR, and PXR (11), suggesting that
recurrent mutations in RXRA could impact the formation and/or function of
these heterodimers and change the expression of their downstream target
genes. Previous reports have shown that cancer samples containing RXRA
p.S427F/Y mutations are associated with enhanced expression of genes
involved in adipogenesis and lipid metabolism, including ACOX1, ACSL1,
ACSL5, FABP4, and HMGS2 (9). These genes are targets of peroxisome
proliferator-activated receptor gamma (PPARG), a member of the PPAR
subfamily of nuclear receptors.
Interestingly, the PPARG gene is focally amplified in 15% of bladder cancer
samples (Supplementary Fig. 1A and (12)). This amplification is strongly
correlated with expression of PPARG (Supplementary Fig. 1B) as well as
expression of PPARG target genes and luminal differentiation markers such as
GATA3, UPK2, ACOX1, and UPK1A (Supplementary Fig. 1C and (13-16)).
PPARG is a master regulator of adipocyte differentiation and controls
4
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RXRA and PPARG in Bladder Cancer
expression of a large set of genes involved in lipid and glucose homeostasis
(12). In contrast to PPARG’s well-characterized activity in adipocytes, however,
little is known about its function in the urinary bladder and in the pathogenesis
of bladder cancer.
The potential risk of bladder cancer upon activation of the PPAR subfamily
of nuclear receptors is controversial, and was first suggested following rodent
toxicity studies testing anti-diabetic PPAR agonists in which numerous glitazar-
class PPARA/PPARG dual agonist compounds were associated with an
increased incidence of bladder cancer (17). In terms of more selective PPARG
agonists, also anti-diabetic drugs with insulin sensitizing activity, the
carcinogenic effect in rodents was also observed with pioglitazone, which has
weak PPARA activity (18), but not with rosiglitazone, which is highly selective
for PPARG (17,19). In a more sensitive, chemically-induced model using the
carcinogen, 4-hydroxybutyl (butyl) nitrosamine (OH-BBN), rosiglitazone was
found to potentiate urinary bladder carcinogenesis in rats compared to OH-BBN
alone (20). It was originally hypothesized that the effects of PPARA/PPARG
dual agonists on promoting bladder cancer was rodent-specific due to indirectly
causing calcium crystal formation in the bladder resulting in urolithiasis (21).
Numerous studies have since examined the incidence of bladder cancer in
humans following the clinical use of these compounds, with some detecting an
increased risk and others concluding there is no increased risk (22,23). The
most comprehensive retrospective study to date showed an increase in the
5
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RXRA and PPARG in Bladder Cancer
hazard ratio for bladder cancer with long-term, high-dose treatment with
pioglitazone (24).
Based on the combined genetic and pharmacologic evidence, we
hypothesized that activation of PPARG is oncogenic in the transitional epithelial
cells of the bladder. We evaluated this by investigating the biological impact of
ectopic expression of mutant alleles of RXRA and PPARG, pharmacologic
ablation of RXRA/PPARG signaling using small molecule perturbagens, and
genetic ablation of RXRA and PPARG using CRISPR/Cas9 gene knockouts.
Our results demonstrate an oncogenic role for PPARG in the development of
luminal bladder cancer, revealing a novel axis that could be exploited for the
development of targeted therapies for this disease.
6
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RXRA and PPARG in Bladder Cancer
Materials and Methods
Chemicals
Rosiglitazone, pioglitazone, tesaglitazar, GW9662, T0070907, UVI3003 and
SR1664 were purchased from Tocris Bioscience (Minneapolis, MN). SR2595
and SR10221 were synthesized according to published methods (25).
GW1929, BADGE (Bisphenol A diglycidyl ether), SR202 and GW6471 were
purchased from Sigma-Aldrich (St. Louis, MO).
Cell lines
The UM-UC-9 cell line was purchased from Sigma-Aldrich (St. Louis, MO).
All other cell lines were obtained from the Cancer Cell Line Encyclopedia
(Broad Institute, Cambridge MA), which obtained them from the original source
and performed cell line authentication (26). To reduce bias from cell culture
medium, all cell lines were maintained in MEMalpha medium supplemented
with 10% Tet-system approved fetal bovine serum (FBS) (Clontech).
Ectopic cDNA expression:
Wild type ORFs for RXRA and PPARGv1 were obtained from the Genomics
Perturbation Platform (Broad Institute, Cambridge MA) in pDONR Gateway
cloning vectors. Various mutant alleles were generated using QuikChange Site-
Directed Mutagenesis (Agilent, Santa Clara CA). ORFs were then subcloned
7
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RXRA and PPARG in Bladder Cancer
into lentiviral expression vectors using Gateway LR Clonase and infectious
lentiviral particles were generated using standard procedures.
SW780 bladder cancer cell line was transduced with a lentiviral vector
encoding the specified RXRA or PPARG ORF under control of constitutive
CMV or EF1α promoter, and stable pools were generated following selection for
blasticidin-resistance. Cell lines were maintained for at least 7 days following
selection prior to expansion for further analysis.
RNA sequencing analysis:
RNA was isolated using RNEasy (Qiagen, Germantown, MD) and an RNA
sequencing library was prepared using NEBNext Ultra Directional RNA Library
Prep Kit for Illumina and NEBNext Multiplex Oligos for Illumina (New England
BioLabs). Sample analysis was performed using a MiSeq System and reagent
kits (Illumina, San Diego, CA) according to the manufacturers protocol.
Sequence data was analyzed using Firehose (Broad Institute, Cambridge MA)
to map transcripts and calculate RPKM (SW780 cDNA expression) or TPM
(UM-UC-9).
For UM-UC-9 RNA sequencing experiment, the resulting reads were used
to calculate transcript abundance in units of TPM (transcripts per million) (27) ,
which were then adjusted using TMM normalization (28) for comparison. Log
fold-change and Mann-Whitney test significance was used to identify
differentially expressed genes between the agonist and inverse-agonist-treated
8
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RXRA and PPARG in Bladder Cancer
samples.
Western blot analysis:
Cells were grown in 6-well plates and harvested using Complete Lysis-M
with protease and phosphatase inhibitors (Roche Applied Science, Germany).
Western blots were performed using standard protocols with semi-dry transfer
Trans-Blot® SD (Bio-Rad Hercules, CA), Li-Cor Odyssey Blocking buffer, and
imaging with LiCor Odyssey Imaging System (LI-COR Lincoln, NE). The anti-
PPARG C26H12, anti-PPARG 81B8, anti-FABP4 D25B3, and anti-CEACAM5
CB30 antibodies were obtained from Cell Signaling Technology (Beverly, MA).
The anti-ACSL5 ab57210 and anti-HMCGS2 EPR8642 antibodies were
obtained from Abcam (Cambridge, MA). The anti-VCL (vinculin) V9264
antibody was obtained from Sigma-Aldrich (St. Louis MO). All primary
antibodies were tested at 1:1000 dilutions, with the exception of anti-VCL,
which was tested at a 1:5000 dilution. Secondary goat anti-mouse 926-68020,
and goat-anti-rabbit 926-32211 antibodies were obtained from Li-Cor
Biosciences (Lincoln, NE) and used at 1:15,000 dilutions.
RT112-FABP4-NLucP reporter gene assay:
Reporter cell line was generated by engineering the NanoLuc gene into the
3’ UTR of FABP4 in RT112/84 cells using CRISPR/Cas9 guided genome
9
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RXRA and PPARG in Bladder Cancer
engineering. Single cell clones were isolated and the clone with the widest
dynamic range selected for use. Assays were performed by seeding 384-well
plates with 10,000 cells per well in MEMalpha containing 10% FBS and dosing
compounds at indicated concentration using the HP D300 digital dispenser
(HP/Tecan). 18-24 hours after dosing with compound, cells were assayed using
NanoGlo Luciferase Assay Reagent (Promega Madison, WI) and plates were
read using an EnVision Multilabel Reader (PerkinElmer Waltham, MA).
Biochemical assays:
The LanthaScreen TR-FRET PPAR gamma Competitive Binding Assay and
LanthaScreen TR-FRET PPAR gamma Coactivator Assay were obtained from
ThermoFisher Scientific (Waltham, MA). Assays were performed according to
the manufacturer’s protocol. In order to assay inverse-agonism, the TR-FRET
PPAR gamma Coactivator assay was modified by the use of fluorescently
labeled corepressor peptides (NCoR1 ID2 peptide, SMRT ID2 peptide) in place
of TRAP220 coactivator peptide to convert from agonist mode (coactivator
recruitment) into inverse-agonist mode (corepressor recruitment).
Proliferation assays:
To enable cell-counting experiments, cell lines were transduced with a
lentiviral vector encoding nuclear-targeted GFP, TagGFP2-H2B (Evrogen,
Moscow, Russia), and stable pools generated following selection for
10
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RXRA and PPARG in Bladder Cancer
puromycin-resistance. Cell lines were maintained for at least 7 days following
selection prior to expansion and seeding into 96-well or 384-well plates for
further analysis. For kinetic proliferation assays, 96-well plates (n = 4 per
condition) were imaged and counted every two hours using IncuCyte Zoom
(Essen BioScience, Ann Arbor MI). Media and compounds were replaced
approximately every 3-4 days. For end-point assays to measure dose-
response, cells were plated in 384-well plates, dosed with compound, and upon
reaching approximately 70-90% confluence in control wells, cells were either
counted using fluorescence imaging (IncuCyte Zoom) or incubated with
CyQuant (ThermoFisher, Waltham, MA) at the indicated time and plates were
read with a fluorescent plate reader.
CRISPR/Cas9 genetic dependency studies:
Cell lines were first transduced with a lentiviral vector encoding hSpCas9
under control of a tetracycline-inducible CMV promoter (CMV-TO,
ThermoFisher Scientific) and stable pools generated following selection for
blasticidin-resistance. Following confirmation of regulated Cas9 expression by
Western blot analysis, the cells were transduced with a lentiviral vector
encoding an sgRNA under control of a tetracycline-inducible H1 promoter (H1-
TO, ThermoFisher Scientific) and double-stable pools were generated following
selection for puromycin-resistance. In addition to providing for regulated sgRNA
expression, these lentiviral vectors also constitutively express one of three
11
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RXRA and PPARG in Bladder Cancer
nuclear-targeted fluorescent proteins to enable unambiguous identification of
transduced cells in subsequent cell counting experiments: YFP-expressing
vectors were used for sgRNAs targeting PPARG; CFP-expressing vectors were
used for sgRNAs targeting non-essential control genes, and RFP-expressing
vectors were used for sgRNAs targeting essential control genes. This approach
is described in more detail elsewhere (Strathdee et al., manuscript in
preparation).
We evaluated 6-8 different sgRNAs per gene of interest using Western blot
analysis in order to identify 2-3 highly active, doxycyline-inducible guides
targeting PPARG (sgPPARG-3: GTCTTCTCAGAATAATAAGG, sgPPARG-6:
GTTTCAGAAATGCCTTGCAG) for use in our experiments. We used KIF11
(sgKIF11-3: GGTGGTGGTGAGATGCAGGT) as an essential control gene, and
an sgRNA targeting PPARG intronic sequence (sgPPARG-
21: GATACTGCTGCATTAGACCAG) was used as a non-essential controls.
Following generation of stable pools of for each sgRNA were combined in
equivalent numbers within replicate wells of 6-well plate and doxycycline was
added to one of the replicates to induce Cas9 and sgRNA. Cells were
passaged every 3-5 days and one replicate maintained under doxycycline
induction, with second replicate maintained in the absence of doxycycline.
During each passage, four replicate wells were passaged into 96-well plates for
fluorescent imaging and fixed with methanol for imaging 1-3 days after passage
into 96-well plates. Changes in relative abundance of cells containing the on-
12
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RXRA and PPARG in Bladder Cancer
test sgRNA, non-essential sgRNA, and essential sgRNA were thus followed by
comparing relative abundance of cells based on fluorescent label (Yellow,
Cyan, Red) through serial passages for a period of 28 days. Cells with stably
transduced TREx inducible vectors were all maintained continuously in
MEMalpha medium containing 10% Tet-system approved FBS (Clontech).
Data availability:
Bladder cancer incidence and survival data was obtained from Howlader N,
Noone AM, Krapcho M, Miller D, Bishop K, Altekruse SF, et al. November 2015
SEER data submission, posted to the SEER web site, April 2016. SEER
Cancer Statistics Review, 1975-2013. National Cancer Institute
The provisional TCGA muscle-invasive urothelial carcinoma data is
available from the Broad Institute TCGA Genome Data Analysis Center.
Analysis-ready standardized TCGA data from Broad GDAC Firehose
2016_01_28 run. https://doi.org/10.7908/C11G0KM9. CCLE Affymetrix U133+2
arrays mRNA expression data is available through
https://portals.broadinstitute.org/ccle/ (26). RNA sequencing data is available
through the National Center for Biotechnology Information BioProject accession
# PRJNA396067.
13
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RXRA and PPARG in Bladder Cancer
Results
PPARG signaling is activated by ectopic expression of RXRA p.S427F/Y
and PPARG p.T447M mutant alleles
To assess the biological effects of mutations in RXRA and PPARG, we
ectopically expressed cDNAs encoding wild-type and mutant alleles of each
gene in the SW780 bladder cancer cell line, which is wild-type for RXRA and
PPARG (26). RXRA hotspot mutant alleles p.S427F and p.S427Y, as well as a
PPARG mutant allele found in RT4 cells, p.T447M in PPARG isoform 1,
NP_005028, also commonly referred to as PPARG p.T475M in isoform 2,
NP_056953.2, were selected for initial testing. We performed RNA sequencing
on parental SW780 cells in comparison with cells expressing wild-type or
mutant PPARG or RXRA alleles. SW780 cells with ectopic expression of RXRA
p.S427F/Y and PPARG p.T447M mutant alleles demonstrated up-regulation of
canonical PPARA and PPARG target genes such as ACSL5, HMGCS2, and
FABP4 (Fig. 1A). Immunoblot assays confirmed significant up-regulation of
several of the corresponding proteins in SW780 cells expressing mutant RXRA
and PPARG alleles (Fig. 1B) even though parental SW780 cells appear to have
elevated expression of PPARG and PPARG target genes when compared to
other bladder cancer cell lines (Fig. 1C). These data are consistent with the
observations of increased expression of these PPAR targets in patient bladder
tumors bearing RXRA hotspot mutations (9).
We also noted a discrete set of genes up-regulated by RXRA p.S427F/Y,
14
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RXRA and PPARG in Bladder Cancer
such as HMGSC2 and CEACAM5, which were minimally regulated by any of
the PPARG alleles. In follow-up immunoblot studies, we included wild-type
PPARA and observed that both HMGCS2 and CEACAM5 were selectively
upregulated upon ectopic expression of PPARA, but not PPARG (Fig. 1B),
indicating that these are likely PPARA targets. We also observed more
pronounced effects of RXRA p.S427F compared to the p.S427Y allele on gene
expression of HMGCS2, FABP4, and others by RNA sequencing (Fig. 1A),
confirmed on the protein level by immunoblot assays (Fig. 1B). This may
indicate a stronger phenotype for RXRA p.S427F, which is consistent with the
higher frequency of this allele in bladder cancer patients (9). Ectopic expression
of other RXRA mutant alleles, selected based on apparent clusters (eg.
p.P231L, p.E233K), and sequence proximity to S427 (p.R421C, p.R421H,
p.R426H, p.G429Y) from pan-cancer genomics analysis (29), had no activity in
these assays (Supplementary Fig. 2).
PPARG inverse-agonists decrease target gene expression in PPARG-
activated cell lines
The study of the phenotype of PPARG-activating genome alterations is
facilitated by a wide variety of compounds that modulate PPARG activity,
including agonists, antagonists, and inverse agonists. PPARG agonists
increase recruitment of coactivators such as CREBBP, PGC1 (PPARGC1A),
and MED1 to the RXRA-PPARG complex, leading to increased expression of
15
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RXRA and PPARG in Bladder Cancer
target genes (Supplementary Fig. 3 - top) (30). PPARG inverse-agonists
recruit co-repressors such as NCOR1, NCOR2, and HDAC3, leading to a
decrease in basal expression of target genes (Supplementary Fig. 3 – bottom)
(30). In contrast, PPARG antagonists have minimal effects on basal receptor
function but are able to prevent both agonists and inverse-agonists from
binding the receptor, thereby blocking their effects (Supplementary Fig. 3) (30).
To evaluate the pharmacological inhibition of PPARG in bladder cancer cell
lines, we tested the impact of known PPARG modulating compounds in gene
expression assays. In preliminary experiments across a panel of PPARG-
activated bladder cancer cell lines (Fig. 1C) we found that dosing bladder
cancer cell lines with T0070907, a PPARG inverse-agonist (31), but not
GW9662, a PPARG antagonist (32), was able to reduce expression of the
canonical PPARG target gene, FABP4 (Supplementary Fig. 4). Although these
compounds have similar potency and selectivity profiles and share a
remarkably similar chemical structure (Supplementary Table 1), they behaved
quite differently in cells.
We engineered an FABP4 reporter cell line to enable higher throughput
assays with which to evaluate PPARG transactivation. Briefly, the NanoLuc
luciferase reporter gene was inserted into the 3’-UTR of the FABP4 gene in the
PPARG-activated RT112/84 bladder cancer cell line using CRISPR/Cas9
mediated homology-directed repair (Supplementary Fig. 5). Since many
compounds that target nuclear receptors are selective modulators which have
16
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RXRA and PPARG in Bladder Cancer
context-dependent activity profiles (30), we used this reporter cell line to
characterize the activity of 13 previously characterized PPARG agonists,
antagonists, and inverse-agonists (18,25,31-40). The full PPARG agonists,
including rosiglitazone, pioglitazone, tesaglitazar, and GW1929, were able to
increase the basal activity of the PPARG reporter from 5.5 to 7.4 fold in this
assay (Figure 2A, indicated in red). The partial agonists, including UVI3003
and SR1664, increased the basal activity of the reporter from 1.4 to 3.1 fold
(Fig. 2A, indicated in black). The antagonists, including BADGE, SR202,
GW9662, and SR2595, had minimal detectable effect on this unstimulated
reporter (Fig. 2A, indicated in light blue). The PPARA-selective inverse agonist
GW6471 exerted a modest inhibitory effect. Finally, the two inverse-agonists
tested, T0070907 and SR10221, reduced basal PPARG reporter activity by 85
to 88 percent (Fig. 2A, indicated in dark blue and green). Interestingly, the
closely related structural analogs (Supplementary Table 1) of these
compounds, GW9662 and SR2595, respectively, were essentially neutral
antagonists in this assay.
To evaluate antagonist and inverse-agonist activity in more detail,
compounds were tested in the presence of a PPARG agonist, rosiglitazone, for
their impact on ligand-activated PPARG reporter activity. Here, the agonists
gave little additional stimulation (Fig. 2B, indicated in black). The antagonists
GW9662 and SR2595 decreased the agonist-induced signal back to the
original baseline (Fig. 2B, indicated in light blue), whereas the inverse-agonists
17
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RXRA and PPARG in Bladder Cancer
T0070907 and SR10221 further reduced the agonist-induced signal 80-90%
below baseline (Fig. 2B, indicated in dark blue and green). These data align
with quantitative PCR analysis of FABP4 gene expression in 5637 and UM-UC-
9 cells treated with PPARG antagonists and inverse-agonists (Supplementary
Fig. 6) and establish that the reporter assay accurately represents the effects of
PPARG modulators on target gene expression in bladder cancer cell lines.
We next evaluated the effects of long-term dosing on the transcriptional
profile of the PPARG-amplified cell line, UM-UC-9. Briefly, UM-UC-9 cells were
treated for 7 days with various PPARG modulators dosed at 500 nM and gene
expression was analyzed using RNA sequencing. Many canonical PPARG
target genes were amongst the top differentially expressed genes that were
upregulated with PPARG agonists and downregulated with inverse-agonists, for
example FABP4 and UCP1 (Supplementary Fig. 7). Genes that were more
abundantly expressed upon treatment with inverse-agonists included ALPP,
SPINK4, and ALDH1A3 (Supplementary Fig. 7). Hierarchical clustering of the
gene expression signatures indicated that GW9662 and SR2595 cluster with
vehicle-treated controls. Therefore, the PPARG inverse-agonists, T0070907
and SR10221, are clearly biologically distinct from the antagonists, GW9662
and SR2595, in bladder cancer cells. While both SR2595 and SR10221 were
described as PPARG inverse-agonists when tested in mouse 3T3-L1 cells (25),
our studies using human bladder cancer cells suggest that SR10221, but not
SR2595, behaves as an inverse-agonist in these cells (Fig. 2 and
18
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RXRA and PPARG in Bladder Cancer
Supplementary Figs. 6-7). In summary, we have characterized the in vitro
pharmacological properties of known PPARG modulators and have identified
two distinct chemotypes with bona-fide inverse-agonist activity in PPARG-
activated bladder cancer cells.
PPARG inverse-agonists induce a repressive complex through inducing
interactions with co-repressor NCOR2
To determine effects on interactions between PPARG and co-regulators, we
tested PPARG modulators in two TR-FRET biochemical interaction assays for
agonism and inverse-agonism. Agonism was quantitated using a co-activator
assay, which measured the interaction between the PPARG ligand-binding
domain and a fluorescently-labeled peptide from TRAP220/MED1. Full
agonists, such as rosiglitazone, tesaglitazar, GW1929, and pioglitazone,
enhanced interaction between PPARG and MED1 coactivator peptide, resulting
in an increase in fluorescent signal from 2.2 to 3.0 fold (Fig. 3A, indicated in
red). The antagonists and partial agonists, BADGE, SR202, GW9662,
UVI3003, and SR1664 had minimal effect in this assay (Fig. 3A, indicated in
gray and light blue). The PPARA-selective inverse-agonist GW6471, PPARG
antagonist SR2595, and PPARG inverse-agonists, T0070907, and SR10221,
exerted a modest inhibitory effect of 40-60%. (Fig. 3A, indicated in dark blue
and gray).
To evaluate inverse-agonism biochemically, we measured ligand-dependent
19
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RXRA and PPARG in Bladder Cancer
interactions between PPARG ligand-binding domain and corepressor peptides
from NCoR/NCOR1 and SMRT/NCOR2. The majority of PPARG partial-
agonists and antagonists had minimal effect on the NCOR2 assay signal (Fig.
3B). PPARG inverse-agonists, T0070907 and SR10221 (Fig. 3B, indicated in
dark blue), increased signal 3-6 fold, while antagonists GW9662 and SR2595
(Fig. 3B, indicated in light blue), induced only a small increase in signal of 1.7-
fold. A decrease in signal of 50-60% was observed with the rosiglitazone,
tesaglitazar, and GW9129 agonists (Fig. 3B, indicated in red).
In addition to the PPARG-NCOR2 interaction assay described above, we
measured interactions between PPARG and a peptide from the corepressor
NCOR1. In the PPARG-NCOR1 interaction assay, T0070907 induced signal 6-
8-fold, while the antagonist GW9662 induced signal 2.5-fold and inverse
agonist, SR10221, induced signal less than 2-fold, and antagonist, SR2595,
had no effect (data not shown). The potent inverse-agonist activity of SR10221
in cellular assays (Fig. 2 and Supplementary Figs. 6-7) and biochemical
PPARG-LBD - NCOR2 assay (Fig. 3B), but not PPARG-LBD - NCOR1
interaction assay (Fig. 3B), suggests that NCOR2 may be the functional co-
repressor mediating PPARG inverse-agonist activity in bladder cancer cells.
PPARG inverse-agonists inhibit the proliferation of PPARG-activated cell
lines
To determine whether PPARG modulators affect the proliferation and/or
20
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RXRA and PPARG in Bladder Cancer
viability of PPARG-activated bladder cancer cell lines, we performed a direct
cell counting-based assay. This assay likely avoids potential artifacts
associated with the use of an ATP content-based assay, given that PPAR
modulators are known to regulate cellular metabolic activity.
Both inverse-agonists, T0070907 and SR10221, significantly reduced
proliferation of UM-UC-9 cells, compared to DMSO control (P<0.001) (Fig. 4A,
indicated in green), with calculated IC50 values of 39 nM and 16 nM. In
contrast, both antagonists tested, GW9662 and SR2595, had no significant
effects on cell proliferation (Fig. 4A, indicated in gray). These IC50 values align
well with the calculated IC50s from both the cell-based reporter gene assay
(Fig. 2A) and the biochemical co-repressor assay (Fig. 3B). They are also close
to the respective reported biochemical IC50s against PPARG, and two orders
of magnitude below that reported for activity against PPARA and PPARD (31),
suggesting that the observed anti-proliferative effects in UM-UC-9 cells are due
to downregulation of PPARG target genes.
We expanded this assay to include an additional 8 representative bladder
cancer cell lines, including cell lines with PPARG amplification, RXRA p.S427F
mutation, activated gene signature, and control cell lines with low level
expression of PPARG and target genes. As we could not always accurately
calculate an IC50 value, we used an alternative quantitative endpoint assay,
which measures the relative number of cells in the DMSO vehicle control
compared to treatment with 100 nM of each compound with analysis performed
21
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RXRA and PPARG in Bladder Cancer
at the time required for the cells to reach 50% confluency in the DMSO control.
Representative data for the UM-UC-9 cell line are shown in Figure 4B, and is
tabulated for the tested bladder cancer cell lines in Table 1. Similar to the full
dose-response assay (Fig. 4A), the T0070907 and SR10221 inverse-agonists
reduce proliferation by 81% and 80% relative to control, whereas the GW9662
and SR2595 antagonists have no effect. This significant (P<0.01) preferential
sensitivity to PPARG inverse-agonists, but not antagonists, is maintained
across all of the PPARG-activated cell lines in the panel, including the RXRA
p.S427F cell line, HT-1197 (41), the PPARG-amplified cell lines, 5637 and UM-
UC-9, and the PPARG-activation gene signature cell lines Cal29, UM-UC-1,
and RT112/84 (Table 1). The SW1710, UM-UC-3, and KU19.19 cells lines that
did not exhibit high expression of PPARG or target genes (Fig. 1C) were
insensitive to PPARG inverse-agonists and antagonists (Table 1). We obtained
similar results with these cell lines in parallel studies using clonogenic assays to
quantify colony forming ability (Supplementary Figure 8). These data reveal that
proliferation of the PPARG-activated subset of bladder cancer cell lines, but not
control bladder cancer cell lines, is dependent on PPARG activity, and inhibition
of this activity with the inverse-agonists, T0070907 or SR10221, results in
decreased proliferative potential.
PPARG-activated cell lines are genetically dependent on PPARG
To test for PPARG dependency in PPARG-activated cell lines with an
22
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RXRA and PPARG in Bladder Cancer
orthogonal approach, we performed CRISPR/Cas9 knockout studies using a
high-precision multicolor competition dependency assay (Strathdee et al.,
manuscript in preparation). Briefly, we first validated that guide RNAs against
PPARG were able to significantly diminish PPARG expression by Western
immunoblot after normalization to loading control vinculin, VCL (Fig. 5A, B). We
next compared the relative effect of knockout of PPARG on cell proliferation to
knockout of an essential gene (KIF11) and to knockout of a non-essential gene
(HPRT or PPIB) or PPARG intron control. The sgRNAs targeting these genes
were cloned into lentiviral vectors that co-express one of three different
fluorescent proteins, YFP, RFP, or CFP, and which allowed for unambiguous
identification of transduced cells in complex pools: PPARG knockout cells were
labeled with YFP, essential control knockout cells were labeled with RFP, and
non-essential (or PPARG intron) control knockout cells were labeled with CFP.
In the competition format, replicate pools of cells are generated at the
beginning of the experiment in which each gene knockout/color are at
equivalent abundance. Changes in relative abundance of each population are
monitored during progressive serial passage by counting fluorescent nuclei
using high-content imaging. Relative changes are plotted as Percent of Control
(POC) of the normalized prevalence of on-test sgRNAs as a percent of non-
essential sgRNA control targeting an intron of PPARG.
Analysis of three bladder cancer cell lines showed a clear PPARG
dependency in PPARG-activated cells. The growth of the SW1710 cell line,
23
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RXRA and PPARG in Bladder Cancer
which shows low PPARG/FABP4 expression (Fig. 1C), is insensitive to PPARG
knockout (Fig. 5C). In contrast, HT-1197 the only known cell line with an RXRA
p.S427F mutation (41), exhibited a strong PPARG-dependency in this CRISPR
competition assay (Fig. 5D). The Cal29 cell line, with a highly activated PPARG
signaling pathway (Fig. 1), also exhibits clear PPARG dependency (Fig. 5E). In
preliminary experiments we determined that the RT4 cell line supported
inadequate hCas9 expression for use in gene knockout experiments, which is
unfortunate since it is the only cell line available with a PPARG p.T447M
mutation. Note that we did not include any cell lines containing PPARG focal
amplifications in order to avoid the well-known copy number sensitivity artifact
inherent to the CRISPR/Cas9 platform (42,43). We conclude that from the
above analyses that PPARG-activated bladder cancer cell lines are dependent
upon a functional PPARG.
Discussion
Recently, genomic analysis of bladder cancer revealed that the PPARG
signaling pathway is significantly activated in tumors, and that this can be
driven by either RXRA p.S427F/Y mutations or PPARG focal amplifications
(9,15). Here we confirm that these alterations, in addition to PPARG p.T447M
mutation which may be emerging as a new hotspot (Supplementary Figure 10),
24
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RXRA and PPARG in Bladder Cancer
activate the PPARG signaling pathway, and that cell lines with the
corresponding mutations are genetically-dependent on PPARG and are also
sensitive to pharmacological inactivation using PPARG inverse-agonists.
One model to explain this data is that these alterations confer ligand-
independent activation of PPARG. In the case of RXRA p.S427F/Y and PPARG
p.T447M mutations this could be achieved by the gain of hydrophobic
interactions that lock PPARG helix 12 into the active conformation,
phenocopying the agonist-induced state in the absence of ligand. Co-crystal
structures of RXRA/PPARG (e.g. PDB ID: 1FM6 and PDB ID: 5JI0) (15,44)
show that the S427 position of RXRA is located in the dimerization interface
with PPARG in the ligand-activated state, directly adjacent to both the T447
residue and c-terminus Y477 residue of PPARG. This positioning is also
conserved in homology models of RXRA/PPARA (45). RXRA p.S427F/Y
mutations may also disrupt interactions between RXRA and its other
heterodimer partners (eg. RARA, VDR, TR), further shifting equilibrium of
RXRA further towards PPARs (15).
It has been established that other mechanisms can lead to ligand-
independent activation of PPARG. For example, signaling by insulin through
the actions of MAP kinases leads to phosphorylation of PPARG in the AF-1
domain which can lead to ligand-independent activation (46). Insulin-dependent
PPARG activation is not sensitive to inhibition by the PPARG antagonist
GW9662, whereas ligand-driven activation by PPARG agonist, cigitazone, is
25
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RXRA and PPARG in Bladder Cancer
sensitive to GW9662 (47). Here we show that PPARG-activated bladder cancer
cells, through PPARG amplification, RXRA p.S427F mutation, or other
unknown mechanisms, are similarly not responsive to antagonists, including
GW9662 and SR2595, but are sensitive to inverse-agonists. Since PPARG
inverse-agonists induce a conformational change in the ligand-binding domain
to actively recruit co-repressors to the complex, these could overcome ligand-
independent signaling, as our studies show.
The impact of PPARG on bladder cancer signaling is supported by the
evidence that PPARA/PPARG dual agonists cause bladder cancer in rodents,
although there are conflicting epidemiological data that PPARA/PPARG
agonists are associated with increased rates of disease in humans (20,22-
24,48).
PPARG as a therapeutic target in bladder cancer can be seen as analogous
to targeting androgen receptor in prostate cancer or estrogen receptor in breast
cancer. One of the hallmarks of luminal cancers is the expression of a ligand-
activated nuclear receptor. Therapeutic targeting of the nuclear receptors in
patients with these cancers can be a very effective therapeutic approach as in
the example of targeting ESR1-positive luminal breast cancer with anti-
estrogens and AR-positive prostate cancer with androgen deprivation therapy.
PPARG agonists upregulate expression of luminal differentiation markers
UPK1A, UPK1B, and KRT20 in primary rat urothelial cells (49). These same
genes, plus GATA3, and FOXA1 are the key luminal markers of bladder cancer
26
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RXRA and PPARG in Bladder Cancer
from human patients (13,14) and bladder cancer cell lines (16). The lineage-
defining role of GATA3, FOXA1, and PPARG in luminal bladder cancer is
reminiscent of luminal breast cancer, in which coordinated expression of
GATA3, FOXA1, and ESR1 enable chromatin remodeling and regulate luminal
gene expression programs (50,51). Whereas in prostate cancer, FOXA1 and
GATA2 (52) coordinately regulate the activity AR (53) and distribution and
selectivity for AR response elements.
The steroid hormone receptors ESR1 and AR are also in the nuclear
receptor superfamily, however, distinct from PPARG, they utilize high affinity
ligands for signaling. Endogenous production of estrogen in breast tissue, and
testosterone / dihyrotestosterone in the testes, are required for receptor
activation. Therefore, in the context of ligand-activation, antagonists of ESR1
and AR are effective therapies for primary cancers. Another effective strategy in
breast and prostate cancer are therapies leading to inhibition of ligand
production such as the use of aromatase inhibitors for treatment of breast
cancer and androgen deprivation therapy for prostate cancer. In contrast,
PPARG does not have a high-affinity endogenous ligand and is considered a
lipid sensor, with low affinity for its ligands (54). Therefore, mechanisms leading
to ligand-independent activation of PPARG, and not ligand-dependent
signaling, appear to be the primary driver of PPARG activity and will require a
different pharmacological properties than in the case of targeting ligand-
27
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RXRA and PPARG in Bladder Cancer
activated ESR1 or AR with a pure antagonist.
Patients treated with anti-estrogen and anti-androgen therapy commonly
develop resistance, with common mechanisms being somatic alterations that
lead to either ligand hypersensitivity or ligand-independent signaling. In the
case of ESR1, recurrent mutations at Y537 mutations lead to ligand-
independent signaling (Robinson et al 2013) and due to being in the ligand-
binding domain, also confer resistance to ESR1 antagonists. In the case of AR,
gene amplification leads to ligand hypersensitivity, whereas point mutations and
alternative splicing can lead to ligand-independent activation (55). In order to
attenuate ligand-independent activation of ESR1, a new class of compounds
was developed that lead to receptor degradation. Selective estrogen receptor
degraders have had promising clinical outcomes, with fulvestrant reaching
clinical approval and providing a new hope for ER+ breast cancer patients
refractory to SERMs and aromatase inhibitors. Based on the fact that there
appears to be high level of ligand-independent PPARG signaling in bladder
cancer, we focused efforts on validating inverse-agonists as a candidate
therapeutic strategy. However, a selective PPARG-destabilizer could be
another promising therapeutic approach worth exploring.
We have demonstrated a genetic and pharmacologic dependence on
PPARG in PPARG-activated, luminal bladder cancer cell lines. Our studies
28
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RXRA and PPARG in Bladder Cancer
provide a well-defined patient population and clear therapeutic hypothesis.
Since PPARG agonists rosiglitazone and pioglitazone are used for the
treatment of diabetes by a mechanism of sensitizing cells to insulin, lowering
blood glucose, and lowering lipid levels (56), one may predict that a PPARG
inverse-agonist may have an opposing effect, eliciting symptoms of diabetes.
Furthermore, patients with deleterious PPARG mutations have an increased
risk for diabetes and can exhibit lipodystrophy and insulin resistance (57). While
there are concerns for on-mechanism complications for PPARG inverse-
agonists as a potential therapy for bladder cancer, there is renewed hope that
rigorous testing and a deep understanding of emerging PPARG biology and
pharmacology (25) can overcome these hurdles through selective receptor
modulation. Recent advances have highlighted a potential role for oncogenic
activation of PPARG in bladder cancer to regulate inflammatory cytokines,
thereby regulating immune cell infiltration and immunosurveillance (15). Further
studies of PPARG in bladder cancer will help to evaluate whether PPARG
inverse agonists can complement conventional and emerging therapies
including other genomically defined therapeutic targets such as FGFR
inhibitors, in addition to immune checkpoint blockade.
29
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RXRA and PPARG in Bladder Cancer
Acknowledgements
The authors would like to thank Xiaoyang Zhang, Josh Francis, Chandra
Pedamallu, Patrick McCarren, Chris Lemke, Aruna Ramachandran Robert
Hilgraf, Stuart Schreiber, and Todd Golub for their helpful discussions and
guidance.
30
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RXRA and PPARG in Bladder Cancer
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40. Xu HE, Stanley TB, Montana VG, Lambert MH, Shearer BG, Cobb JE, et al. Structural basis for antagonist‐mediated recruitment of nuclear co‐ repressors by PPARalpha. Nature 2002;415:813‐7 41. Forbes SA, Beare D, Boutselakis H, Bamford S, Bindal N, Tate J, et al. COSMIC: somatic cancer genetics at high‐resolution. Nucleic Acids Research 2017;45:D777‐D83 42. Aguirre AJ, Meyers RM, Weir BA, Vazquez F, Zhang CZ, Ben‐David U, et al. Genomic Copy Number Dictates a Gene‐Independent Cell Response to CRISPR/Cas9 Targeting. Cancer Discov 2016;6:914‐29 43. Munoz DM, Cassiani PJ, Li L, Billy E, Korn JM, Jones MD, et al. CRISPR Screens Provide a Comprehensive Assessment of Cancer Vulnerabilities but Generate False‐Positive Hits for Highly Amplified Genomic Regions. Cancer Discov 2016;6:900‐13 44. Gampe RT, Jr., Montana VG, Lambert MH, Miller AB, Bledsoe RK, Milburn MV, et al. Asymmetry in the PPARgamma/RXRalpha crystal structure reveals the molecular basis of heterodimerization among nuclear receptors. Mol Cell 2000;5:545‐55 45. Venalainen T, Molnar F, Oostenbrink C, Carlberg C, Perakyla M. Molecular mechanism of allosteric communication in the human PPARalpha‐RXRalpha heterodimer. Proteins 2010;78:873‐87 46. Zhang B, Berger J, Zhou G, Elbrecht A, Biswas S, White‐Carrington S, et al. Insulin‐ and Mitogen‐activated Protein Kinase‐mediated Phosphorylation and Activation of Peroxisome Proliferator‐activated Receptor Journal of Biological Chemistry 1996;271:31771‐4 47. Al‐Rasheed NM, Chana RS, Baines RJ, Willars GB, Brunskill NJ. Ligand‐ independent activation of peroxisome proliferator‐activated receptor‐ gamma by insulin and C‐peptide in kidney proximal tubular cells: dependent on phosphatidylinositol 3‐kinase activity. J Biol Chem 2004;279:49747‐54 48. Turner RM, Kwok CS, Chen‐Turner C, Maduakor CA, Singh S, Loke YK. Thiazolidinediones and associated risk of bladder cancer: a systematic review and meta‐analysis. Br J Clin Pharmacol 2014;78:258‐73 49. Varley CL, Southgate J. Effects of PPAR agonists on proliferation and differentiation in human urothelium. Exp Toxicol Pathol 2008;60:435‐41 50. Theodorou V, Stark R, Menon S, Carroll JS. GATA3 acts upstream of FOXA1 in mediating ESR1 binding by shaping enhancer accessibility. Genome Res 2013;23:12‐22 51. Eeckhoute J, Keeton EK, Lupien M, Krum SA, Carroll JS, Brown M. Positive cross‐regulatory loop ties GATA‐3 to estrogen receptor alpha expression in breast cancer. Cancer Res 2007;67:6477‐83 52. Zhao JC, Fong KW, Jin HJ, Yang YA, Kim J, Yu J. FOXA1 acts upstream of GATA2 and AR in hormonal regulation of gene expression. Oncogene 2016;35:4335‐ 44 53. Jin HJ, Zhao JC, Wu L, Kim J, Yu J. Cooperativity and equilibrium with FOXA1 define the androgen receptor transcriptional program. Nat Commun 34
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RXRA and PPARG in Bladder Cancer
Table 1
Cell Line Pathway Alteration GW9662 SR2595 T0070907 SR10221
HT‐1197 RXRA p.S427F 127 78 48** 64*
5637 PPARG amplified 93 117 51** 73**
UM‐UC‐9 PPARG amplified 108 97 19** 20**
RT112/84 PPARG signature 98 101 69** 80**
UM‐UC‐1 PPARG signature 96 84 47** 62**
Cal29 PPARG signature 97 86 55** 74*
SW1710 Not altered 99 91 96 81
KU19.19 Not altered 85 91 95 91
UM‐UC‐3 Not altered 92 102 91 96 *, P <0.01 ** , P<0.001
Relative proliferation rate of bladder cancer cell lines treated with PPARG
inhibitors at 100nM compared to DMSO vehicle, reported as percent of vehicle
control (POC), in long-term kinetic proliferation assays. Percent of DMSO
control was calculated by determining the relative number of cells for treatment
versus DMSO control at the timepoint where DMSO control reached 50%
confluence (see Fig. 4B for graphical representation) by counting fluorescently
labeled nuclei (IncuCyte Zoom). Significant differences in cell number for test
sample relative to DMSO control were calculated using two-way ANOVA with
Dunnett’s multiple comparison test(*P<0.01, **P <0.001).
36
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RXRA and PPARG in Bladder Cancer
Figure Legends
Figure 1. PPARG signaling is activated by ectopic expression of RXRA
p.S427F/Y and PPARG p.T447M mutant alleles. A, RNA expression (RSEM)
of selected genes that were differentially expressed when comparing parental
SW780 cells, cells with ectopic expression of wild-type RXRA and PPARG, and
cells expressing mutant alleles of RXRA and PPARG. B, Immunoblot analysis
of lysates from SW780 cells ectopically expressing RXRA and PPARG wild-
type and activating mutant alleles. C, Heatmap of Cancer Cell Line
Encyclopedia (CCLE) gene-centric RMA-normalized mRNA expression data
(26) across bladder cancer cell lines indicating luminal differentiation markers
and PPARG target genes. The samples were grouped by hierarchical clustering
of columns using the Morpheus software package
(https://software.broadinstitute.org/morpheus/).
Figure 2. PPARG inverse-agonists decrease basal activity by inducing
active repression. PPARG-activated RT112/84 bladder cancer cell line
engineered to contain the NanoLuc gene in the 3’ UTR of a canonical PPARG
target gene, FABP4, was used to profile the effect of compounds on PPARG-
dependent gene transactivation. A, Dose-response testing of panel of PPARG
modulators in the RT112/84 FABP4-NLucP reporter assay under unstimulated
conditions to evaluate activity of agonists and inverse-agonists. B, Antagonist
37
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RXRA and PPARG in Bladder Cancer
mode dose-response testing of panel of PPARG modulators in the RT112/84
FABP4-NLucP reporter assay performed by combined dosing of the PPARG
agonist, rosiglitazone at the EC50, 20nM, in combination with a dose-response
for test compounds, as indicated.
Figure 3. PPARG inverse-agonists induce a repressive complex by
blocking interactions with coactivators and inducing interactions with co-
repressor NCOR2. A TR-FRET assay was used to evaluate the ligand-
dependent interactions between Terbium-labeled PPARG ligand binding
domain (PPARG-LBD) and fluorescein-labeled peptides derived from nuclear
receptor coregulators, as indicated. A, Dose-response testing of a panel of
PPARG modulators in an agonist biochemical model evaluating in a PPARG-
LBD - TRAP220 (MED1) co-activator peptide interaction assay to measure
agonist-induced interactions, or inverse-agonist induced decrease in
interactions. B, Dose-response testing of a panel of PPARG modulators in an
inverse-agonist biochemical model evaluating PPARG LBD – SMRT (NCOR2)
co-repressor interactions.
Figure 4. PPARG inverse-agonists, but not antagonists, inhibit
proliferation of PPARG-activated bladder cancer cell lines. A, proliferation
assay measuring dose-dependent effect of PPARG modulators on cell number
in UM-UC-9 cells using high content imaging to count fluorescently-labeled
38
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RXRA and PPARG in Bladder Cancer
nuclei. B, kinetic proliferation assay measuring the effect of 100nM modulator
on growth rate over time in UM-UC-9 with graphical representation of percent of
control calculation. Fluorescently labeled nuclei were counted using IncuCyte
Zoom every 2 hours (n= 4 replicates per condition). Data are represented as
mean ± SD.
Figure 5. Cell lines with PPARG activation are dependent on PPARG. A,
PPARG sgRNA’s 3, and 6 knock out PPARG protein in 5637 cells. A, Western
immunoblot of PPARG and loading control VCL. B, Quantification of PPARG
Western blot signal after normalization to VCL, reported as ratio of integrated
fluorescence intensity K counts and was performed using Li-Cor Odyssey
Application Software version 3.0.30 (Li-Cor, Lincoln NE). C-E, CRISPR/Cas9
competition screen to measure relative proliferation of cells harboring sgRNA
targeting PPARG (yellow), non-essential control of PPARG intron (cyan), and
essential control gene KIF11 (red). Cells lines were infected with lentivirus
encoding both fluorescent marker and sgRNA prior to pooling cells for assay.
Cell lines include B, HT-1997 (RXRA p.S427F), C, Cal 29 (PPARG-activated)
and D, SW1710 (not altered, neutral control). Data are represented as POC,
normalized prevalence of test sgRNAs as a percent of the non-essential
PPARG intron control sgRNA (mean ± SD).
39
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Genomic activation of PPARG reveals a candidate therapeutic axis in bladder cancer
Jonathan T Goldstein, Ashton C. Berger, Juliann Shih, et al.
Cancer Res Published OnlineFirst September 18, 2017.
Updated version Access the most recent version of this article at: doi:10.1158/0008-5472.CAN-17-1701
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